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How and When Do Insects Rely on Endogenous

Oct 14, 2015 - species of insects (adult grasshoppers, crickets, cockroaches, and larval beetles and moths) ... role in study design, data collection and analyses, .... and randomly assigned to one of two diet treatment groups (Table 1). .... longevity, by plotting the relationships between LT50 versus lipidpeak, proteinpeak, ...

RESEARCH ARTICLE

How and When Do Insects Rely on Endogenous Protein and Lipid Resources during Lethal Bouts of Starvation? A New Application for 13C-Breath testing Marshall D. McCue1*, R. Marena Guzman1, Celeste A. Passement1, Goggy Davidowitz2 1 St. Mary’s University, Department of Biological Sciences, San Antonio, Texas, United States of America, 2 University of Arizona, Department of Entomology, Tucson, Arizona, United States of America * [email protected]

Most of our understanding about the physiology of fasting and starvation comes from studies of vertebrates; however, for ethical reasons, studies that monitor vertebrates through the lethal endpoint are scant. Insects are convenient models to characterize the comparative strategies used to cope with starvation because they have diverse life histories and have evolved under the omnipresent challenge of food limitation. Moreover, we can study the physiology of starvation through its natural endpoint. In this study we raised populations of five species of insects (adult grasshoppers, crickets, cockroaches, and larval beetles and moths) on diets labeled with either 13C-palmitic acid or 13C-leucine to isotopically enrich the lipids or the proteins in their bodies, respectively. The insects were allowed to become postabsorptive and then starved. We periodically measured the δ13C of the exhaled breath to characterize how each species adjusted their reliance on endogenous lipids and proteins as energy sources. We found that starving insects employ a wide range of strategies for regulating lipid and protein oxidation. All of the insects except for the beetle larvae were capable of sharply reducing reliance on protein oxidation; however, this protein sparing strategy was usually unsustainable during the entire starvation period. All insects increased their reliance on lipid oxidation, but while some species (grasshoppers, cockroaches, and beetle larvae) were still relying extensively on lipids at the time of death, other species (crickets and moth larvae) allowed rates of lipid oxidation to return to prestarvation levels. Although lipids and proteins are critical metabolic fuels for both vertebrates and insects, insects apparently exhibit a much wider range of strategies for rationing these limited resources during starvation.

Funding: Funding for this research was provided by the Biaggini Endowment and a Faculty Grant both awarded to MDM from St. Mary’s University and NSFgrant IOS-1053318 to GD. The funders had no role in study design, data collection and analyses, decision to publish, or preparation of the manuscript.

Introduction

Competing Interests: The authors have declared that no competing interests exist.

All animals face the possibility of food limitation during which they must rely solely on endogenous nutrients to fuel their continued metabolic demands. Most of our understanding about

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how animals respond to starvation comes from studies of vertebrates (see reviews by [1–6]). While vertebrates demonstrate a number of physiological strategies for surviving starvation these strategies may not necessarily be generalizable to invertebrates such as insects that have also evolved under the omnipresent challenges of food limitation (e.g., [7–11]). Insects outnumber vertebrates in number, species, and biomass [12]. Because they play central roles in most terrestrial and aquatic food webs [13] it is important to understand how these animals cope with fluctuating food resources. Although the diversity of starvation tolerance among insects may be no less impressive than that documented among vertebrate animals, we know quite little about how they physiologically respond to starvation [14–18]; in fact, recent reviews have explicitly cited the need for additional comparative studies of starvation among insects and other invertebrates [19–21].

Characterizing the progression of starvation Can researchers use the same physiological toolbox developed for vertebrate animals to study starvation in insects? Starvation-induced changes in blood metabolites used routinely in vertebrates (e.g., glucose, ketone bodies, and nitrogen metabolites) are rarely reported for insects in part because of logistical issues related to body size and peculiarities of hemolymph metabolites (e.g., trehalose and proline [18,22]), and perhaps also in response to the growing awareness that circulating metabolites offer limited mechanistic insight into systemic nutrient fluxes [3,23,24]. Indeed, studies have shown that starving insects mobilize glycogen and triglycerides stored in their fat bodies [17,18,22,25,26], but destructive sampling of body composition precludes continual measurements of fuel oxidation over long periods. Changes in respiratory exchange ratios (RERs) of starving insects are often difficult to quantitatively interpret [15,19,27] and therefore may preclude accurate assessments of changes in metabolic fuel mixtures [28–30]. This limitation is confounded with the fact that VCO2 can usually be measured in insects with greater accuracy than VO2 [31]. Other non-invasive approaches like NMR microscopy can be used to quantify changes in the fat and water content in small insects over time and therefore may be used to estimate lipid oxidation [32]; but the method is not suitable for tracking changes in protein use or for making measurements in large numbers of individuals. Quantitative magnetic resonance (QMR) has been shown to be suitable for accurate measures of lean mass in large insects [33], but it is not suitable for quantifying the lipid content in their bodies. Recently developed approaches where different nutrient pools in the body (e.g., carbohydrates, lipids, and proteins) are selectively enriched with a stable isotope (e.g., 13C) have been coupled with 13C-breath testing to characterize the starvation-induced changes in metabolic fuels among birds and mammals [34,35], but they have not yet been used to study starvation in insects. Here we examine whether insects of different species and age classes exhibit strategies of rationing oxidative fuels that are generally similar to those seen among most vertebrates. Based on the traditional three-phase paradigm about fuel switching (reviewed in [1,36–38]), it is likely that carbohydrates in the hemolymph provide a readily available fuel source and therefore lipid and protein oxidation are minimal at the onset of starvation. As starvation progresses, lipids are expected to become the predominant source of metabolic energy. Protein oxidation is expected to increase dramatically, but only during the lattermost phases of starvation when most, or all, of the lipid reserves have been depleted. Because of the ethical concerns of starving vertebrate animals to death, this pre-mortem increase in protein oxidation, often used to delimit the transition from phase II to phase III, is rarely documented in vertebrates. However, insects are convenient models in which to test the prediction that death from starvation is invariably preceded by a dramatic, unsustainable increase in protein oxidation (sensu [39]).

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Species selection In contrast to vertebrates in which much of the work on fuel use during starvation has been done, insects have a greater diversity of life history strategies for growth and development. Insects of some orders are hemimetabolous, whereas others are holometabolous. In general, juveniles of hemimetabolous insects eat the same food as do the adults, whereas juveniles of holometabolous insects typically live in very different habitats and eat substantially different foods than do the adults. Some insects are capital breeders in which (nearly) all of the resources used for reproduction are acquired during the juvenile (larval) phase of growth [40,41]. In contrast, income breeders accumulate resources used in reproduction during the adult stage. Insects vary dramatically in size and insect growth is exponential [42] so that nearly all of growth occurs in the last larval instar [43]. Last, longevity of the juvenile stage relative to the adult stage and longevity of lifespan in general is extremely variable among insect species. To account for this complexity of life histories we chose five species of insects that span a range of life history strategies with the restriction that we could rear sufficient numbers to accommodate the study. The Madagascar hissing cockroach, Gromphadorhina portentosa is hemimetabolous, large sized and relatively longed lived. The eastern lubber grasshopper, Romalea microptera is also hemimetabolous and large sized, but has a shorter lifespan. The house cricket, Acheta domesticus, is hemimetabolous but smaller with a shorter lifespan than the grasshoppers. The darkling beetle, Zophobis morio is a small holometabolous income breeder. The hawk moth, Manduca sexta, is a large holometabolous capital breeder. It was not our intention to exhaustively sample all insect life histories, rather, the insects used in this study represent a limited subset of insect life history strategies that represent a significant diversity of strategies to provide a picture of possible strategies of fuel use during starvation. As mentioned above, there are no studies of starvation strategies in insects. With this perspective as a starting point, subsequent studies can test specific hypotheses of starvation strategies across taxa, life history stages, and environmental conditions.

Methods Animals and experimental diets The five phylogenetically diverse species of insects were raised in the laboratory on one of two 13 C-labeled tracers (13C-1-palmitic acid or 13C-1-L-leucine; Cambridge Isotope Laboratories, Tewksbury, MA) with the aim of isotopically enriching either their body lipids or proteins, respectively. They were then starved while we measured the δ13C in their exhaled breath to track how starvation affected their reliance on endogenous lipid and protein oxidation. Madagascar hissing cockroaches (G. portentosa) nymphs (n = 300; age 1–14 days; 10– 20mg) were selected from a larger colony maintained for several generations in our laboratory and randomly assigned to one of two diet treatment groups (Table 1). They were raised to adulthood (4–5 months of age) on a base diet consisting of ground chick starter food (Nutrena; Naturewise) supplemented with one of the two 13C-labeled tracers. Lots of n = 20 adult cockroaches from each population were placed into five metabolic chambers (1.5 L) where they were starved. The bottom of each metabolic chamber consisted of a false floor of 1cm×1cm wire mesh that allowed feces to pass through thereby preventing coprophagy. Segments of PVC tubing were also placed inside the metabolic chambers to provide a hiding place where they naturally reside during the day. The cockroaches were given 24 hours to become postabsorptive before beginning the breath collection. House crickets (A. domesticus) nymphs (n = 500; age 2 weeks) were obtained from a commercial vendor (Fluker Farms; Port Allen, LA) and were randomly divided into one of two diet

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Table 1. Summary of the five insect species used and their experimental diets used to isotopically enrich their tissues. Species Gromphadorhina portentosa

Base diet Chick food

Acheta domesticus

Tilapia chow

Romalea microptera

Romaine lettuce

Manduca sexta Zophobis morio

Prepared diet Bran+Tilapia chow

13

C-1-L-leucine -1

13

C-1-palmitic acid 1 g kg-1

1 g kg

-1

1.667g kg

1 g kg-1

variable

variable

-1

8 g kg-1

-1

1 g kg-1

8 g kg

1 g kg

Bran was mixed in with the 13C-labeled tilapia chow for the larval beetles. doi:10.1371/journal.pone.0140053.t001

treatment groups (Table 1). They were raised to adulthood (6-weeks of age) on a base diet of ground tilapia pellets mixed with one of the two 13C-labeled tracers. Lots of n = 40 adult crickets from each population were relocated into five metabolic chambers (1.0 L) where they were starved. The metabolic chambers were lined with 1cm×1cm plastic mesh to provide threedimensional contour. The crickets were given 12 hours to become postabsorptive before beginning the breath collection. Eastern lubber grasshoppers (R. microptera) nymphs (n = 80, male, 2–3cm) were collected by Prof. John Hatle with permission of a private property owner in Jacksonville, Florida; no collecting permit was required. They were randomly assigned to one of two diet treatment groups and fed a base diet of romaine lettuce leaves lightly dusted with one of the two 13C-labeled tracers (Table 1). They were raised to adulthood over the following 6 weeks. Individual grasshoppers were placed inside 100ml plastic syringes that served as metabolic chambers. The grasshoppers were given 24 hours to become postabsorptive before beginning the breath collection. Darkling beetles (Z. morio) larvae (mealworms; n = 100, 99.9% water and does not provide a significant energy source during starvation. The metabolic chambers were ported to allow fresh air to passively circulate, but these ports were closed prior to gas sampling to ensure CO2 concentrations were between 2 to 4% at the time of breath collection. Gas samples were collected using gas tight syringes and injected into evacuated 12ml ExetainerTM vials (Labco Limited; Ceredigion, UK). The metabolic cages were cleaned every other day to minimize microbial growth. The starvation trials were stopped once half of the experimental animals succumbed to starvation (i.e., lethal time; LT50). Because the LT50 includes total time food was withheld, it includes the period during which the insects were becoming postabsorptive and thus overestimates the actual ‘starvation’ period by 12 (cricket, and beetle and moth larvae) or 24 (grasshopper, cockroach) hours as described above. The δ13C in each gas sample was analyzed using a HeliFAN Plus nondispersive infrared spectrometer (Fischer, ANalysen Instrumente GmbH; Germany) interfaced with a FANas autosampler. The 13C-analyzer was internally and externally calibrated at the start of each batch of samples. Vials containing a standard gas (2.5% CO2; Mesa Specialty Gases) were analyzed after every five unknown breath samples to identify and correct for analytical drift. Postabsorptive insects were selected from each population and killed at the start of the starvation trials to measure their initial tissue δ13C. The carcasses were dried to a constant mass at 70°C in a convection oven, ground with a mortar and pestle, and further homogenized using a dental amalgamator. The lipid and lean fractions of the carcasses were chemically isolated using a modified Folch extraction method [46]. The δ13C of each fraction was analyzed at the University of Arizona using a Picarro (Sunnyvale, CA) G2121-i Cavity Ring Down Spectroscopy (CRDS) δ13C stable isotope analyzer with the A0502 ambient CO2 interface, an A0201 Combustion Module, and an A0301gas interface (CM-CRDS). All 13C concentrations are expressed in δ13CVPDB [47,48].

Calculations and statistics Because the amount of 13C in the exhaled breath is primarily a function of the absolute concentration of the 13C in the diets, reporting of the actual δ13C of the breath provides only limited insight [49]. It is more informative to document how the δ13C of the breath changes as the insects gradually transition from the nourished state to starvation. We therefore used the δ13C from the first, postabsorptive breath samples as a starting reference point for each species. All of the subsequent δ13C breath values during starvation are expressed in terms of that reference point. For example, positive values mean that the breath of the starving animal contained a higher concentration of 13C than the recently postabsorptive animals, whereas negative values mean that the breath contained a lower concentration of 13C. We used a one sample t-test against a mean (SigmaPlot 12, San Jose, CA) at each time point to determine whether the δ13C in the breath significantly differed from the prestarvation values. Evaluations were made using Because we were asking whether a specific time point along a specific sequence was different from the initial value (and not more generally which values were different) there was no need for a Bonferroni-type correction and therefore α = 0.05. 13 C-breath testing relies on the assumption that the oxidation and subsequent excretion of 13 CO2 from the 13C-palmitic acid and 13C-leucine tracers is proportional to the rates of lipid and protein oxidation in the whole body. This assumption is not unrealistic because these two monomers comprise such a large component of their parent nutrient pools. For example, palmitic acid accounts for approximately 30% (21.8–46.5%) of the fatty acids in insects used for human consumption [50] and leucine accounts for approximately 7% (1–9%) of all of the amino acid residues in body proteins [50]. It is worth noting that studies of vertebrates have

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shown that the relative amount of leucine, an essential amino acid, in the body proteins remained constant despite substantial protein losses over a six-month starvation period [51] supporting our contention that leucine content is an accurate proxy for total protein levels. The δ13C of the exhaled breath of starving animals, either reported in absolute terms or in terms of the difference between the freshly postabsorptive and the starved states as described above, follows highly complex time-dependent functions. The complexities of these functions are not unlike those seen during the specific dynamic action (SDA) response in postprandial animals. We therefore borrowed and modified some of the descriptive variables routinely used to characterize SDA responses among animals (see [52,53]) to describe the changes in lipid and protein oxidation during starvation. Specifically, we defined several metrics including: • LT50:- The time (in days) after which food was removed required for 50% of the individuals of a species to succumb to starvation. • lipidpeak:- The time (in days) at which peak lipid oxidation occurred denoted by the maximal δ13C in the breath of the palmitic acid treatment groups. • lipidpeak% LT50:- The relative timing of the lipidpeak expressed in terms of a percent of LT50. • proteinminimum:- The time (in days) at which minimum protein oxidation occurred denoted by the minimum δ13C in the breath of the leucine treatment groups. • proteinminimum% LT50:-The relative timing of the proteinminimum expressed in terms of a percent of LT50. • sparingduration:- The time (in days) during which protein sparing was occurring. Protein sparing was defined as the period during which the mean δ13C in the breath of the leucine treatment was lower (negative) during starvation than in freshly postabsorptive insects. • sparingduration % LT50:- The relative length of sparingduration expressed in terms of a percent of LT50. • proteinpeak:- The time (in days) at which peak protein oxidation occurred denoted by the maximal δ13C in the breath of the leucine treatment groups. • proteinpeak % LT50:- The relative timing of proteinpeak expressed in terms of a percent of LT50.

Strategies for maximal longevity We addressed the question of what the best strategies of resource utilization are to maximize longevity, by plotting the relationships between LT50 versus lipidpeak, proteinpeak, and sparingduration. We fit either a linear or a non-linear exponential regression whichever had the higher coefficient of determination (R2).

Results Tissue enrichment The tissues of the growing insects became enriched in 13C roughly in the proportions that their respective diets were isotopically enriched (Table 2). For example, the highest δ13C values were seen in tissues of the moth larvae raised on 8g kg-1 (dry mass) of tracers in their prepared diet and the lowest enrichments were seen in the tissues of the beetle larvae raised on unlabeled bran supplemented with tilapia food spiked with 1g kg-1 of 13C-tracer. In general the 13C from

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Table 2. Isotopic enrichment of the lean and lipid fractions in the whole bodies of insects raised on diets supplemented with either 13C-leucine or 13 C-palmitic acid. See Table 1 for dosing levels. Species

Treatment

G. portentosa

A. domesticus

R. microptera

Z. morio

M. sexta

Fraction

δ13C

s.d. 3.5

palmitic acid

lipid

22.4

palmitic acid

lean

-12.8

0.9

leucine

lipid

-21.5

0.2

leucine

lean

3.5

4.3

palmitic acid

lipid

33.7

1.6

palmitic acid

lean

-13.0

1.2

leucine

lipid

-22.5

0.9

leucine

lean

29.7

4.1 2.9

palmitic acid

lipid

39.3

palmitic acid

lean

-12.1

1.6

leucine

lipid

-16.8

1.6 3.4

leucine

lean

43.4

palmitic acid

lipid

33.0

2.7

palmitic acid

lean

-13.0

1.3

leucine

lipid

-18.1

0.9

leucine

lean

52.1

3.8

palmitic acid

lipid

176.6

72.3

palmitic acid

lean

5.9

8.5

leucine

lipid

-2.7

3.3

leucine

lean

123.3

61.7

doi:10.1371/journal.pone.0140053.t002

the leucine tracer remained in the nonlipid pool and the 13C from the palmitic acid tracer remained in the lipid pool (Table 2). See the Discussion for more details.

Oxidation of endogenous lipids All of the insects increased their rate of lipid oxidation at the onset of starvation, but the responses thereafter were species-specific. The starving grasshoppers quickly increased lipid oxidation and maintained a high reliance on lipid oxidation that peaked at 11 days (lipidpeak), 69% of the LT50 (Table 3). Immediately preceding death their reliance on lipids remained significantly higher than prestarvation values (Fig 1A). The cockroaches, crickets, and larval moths exhibited their lipidpeak during the first third of the starvation period (Table 3), but near the point at which they succumbed to starvation their reliance on lipids was varied. Immediately preceding death the cockroaches exhibited rates of lipid oxidation that were significantly higher than prestarvation levels (Fig 1B). In contrast, after reaching peak lipid oxidation early in the starvation period, the moth larvae gradually reduced their reliance on lipid oxidation Table 3. Measures of starvation performance and lipid and protein oxidation. See Methods for details about calculations. LT50 (days)

Lipidpeak (days)

G. portentosa

52

A. domesticus

5

Species

Lipidpeak (%LD50)

Proteinminimum (days)

Proteinminimum (%LD50)

11.5

22.1

8.5

16.3

1.5

30.0

1

20.0

Sparingduration (days)

Sparingduration (%LD50)

Proteinpeak (days)

Proteinpeak (%LD50)

21

40.4

52

100.0

1.5

30.0

5

100.0 100.0

R. microptera

16

11

68.8

4

25.0

14

87.5

16

Z. morio

5.5

4.5

81.8

5

90.9

0

0.0

1

18.2

M. sexta

3

1

33.3

3

100.0

2.5

83.3

0.5

16.7

doi:10.1371/journal.pone.0140053.t003

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Fig 1. Starvation-induced changes in the δ13C of the exhaled breath of insects. Adult grasshoppers (A) and cockroaches (B) raised on diets supplemented with 13C-palmitic acid tracers (grey) or 13C-leucine tracers (black). The dashed line represents the δ13C of the breath in postabsorptive insects at the start of fasting. Error bars represent standard deviations. The bold lines indicate time points at which fasting values were statistically different from the prefasting values according to two-way, one-sample t-tests. doi:10.1371/journal.pone.0140053.g001

(Fig 2C). In the moth larvae these values were not significantly different form the prestarvation values (Fig 2A). The beetle larvae were unique in that they did not rapidly increase lipid oxidation at the onset of starvation and only reached peak lipid oxidation (lipidpeak) near the point of death (Fig 2B). At no time point did any of the starving insects exhibit rates of lipid

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Fig 2. Starvation-induced changes in the δ13C of the exhaled breath of insects. Adult crickets (A) and larval beetles (B) and moths (C) raised on diets supplemented with 13C-palmitic acid tracers (grey) or 13Cleucine tracers (black). The dashed line represents the δ13C of the breath in postabsorptive insects at the start of fasting. Error bars represent standard deviations. The bold lines indicate time points at which fasting values were statistically different from the prefasting values according to two-way, one-sample t-tests. doi:10.1371/journal.pone.0140053.g002

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oxidation that were significantly lower than the prestarvation states; however, this was not the case with protein oxidation (see below).

Oxidation of endogenous proteins The responses with regard to protein oxidation were more complex than those described above for lipid oxidation. Four of the five insect species exhibited some tendency for protein sparing whereby their reliance on protein oxidation was lower than it was in the prestarvation state, but this response was only significant in the grasshoppers, cockroaches, and moth larvae. Proteinminimum occurred during the first quarter of the experiment in cockroaches, crickets, and grasshoppers. These three species were apparently able to spare proteins for 30% to 88% of the starvation period (sparingduration; Table 3). Although the moth larvae were also able to spare proteins for most of the experiment, they exhibited minimum rates of protein oxidation only at the end of the experiment (Fig 2C). The beetle larvae were apparently unable to reduce protein oxidation below prestarvation values at any time point (Fig 2B). Notably, the beetle larvae exhibited peak protein oxidation 18% into the experiment (proteinpeak; Table 2)–a point at which most other species were exhibiting protein sparing. At the time of death the reliance on protein oxidation was as varied among the five species as it was for lipid oxidation. For example, the cockroaches and crickets were oxidizing proteins at or near their peak rates that were also significantly higher than prestarvation rates. In contrast, the grasshoppers and beetle larvae relied on protein oxidation at the time of death to an extent similar to their prestarvation levels. The moth larvae were unique in that they exhibited their minimal reliance on protein oxidation immediately preceding death at rates that were significantly lower than prestarvation rates.

Discussion 13 C Tracer integration into the body The 13C-leucine and 13C-palmitic acid tracers added to the insect diets were effective at enriching the lean and lipid fractions in the bodies, respectively (Table 2). Experimentally controlling the dose of 13C-tracers was more effective for species that consumed a homogenized, prepared diet (Table 1) than those that specialized on bran or fresh lettuce (mealworms and grasshoppers, respectively), however it may be possible to individually force feed a fixed amount of tracer to larger species (e.g., grasshoppers; J.D. Hatle, unpublished observation). Interestingly, in most cases the δ13C of the body lipids of the palmitic acid groups was higher than the δ13C of the lean tissue of the conspecific leucine groups (Table 2). The higher tissue 13C enrichment within the lipids was initially surprising given that the molecular mass of palmitic acid is nearly twice that of leucine and thus the insects in the leucine treatments ultimately consumed nearly twice the number of tracer-derived 13C-atoms than those in the palmitic acid treatment. We did not quantify the rates of exogenous (i.e., dietary) tracer oxidation in the insects during growth, but previous studies on birds [54,55], rodents [56], and bats [57], have shown that exogenous leucine is oxidized at a rate nearly an order of magnitude greater

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Fig 3. Correlations between fuel use and longevity. Relationships between starvation tolerance (LT50) and physiological metrics related to fuel oxidation in five species of insects (data from Table 2). The dashed lines illustrate isometry. doi:10.1371/journal.pone.0140053.g003

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than palmitic acid during the postprandial phase. Comparisons of the oxidation of 13C-labeled leucine and oleic acid (another common fatty acid) in postprandial grasshoppers shows that 1.6% and 0.64% of the exogenous 13C was recovered, respectively, in the breath by 11 hours [58]. Previous studies of crickets injected with 14C-radiolabeled tracers into their hemocoel showed that the amino acid, glycine was oxidized about three-fold more rapidly than palmitic acid [59,60]. Consequently, the observed differences in δ13C between the lipid and lean pools in the nourished insects may be explained by the fact that less exogenous palmitic acid was oxidized thereby leaving more to be allocated to the growing tissues [49]. A negligible amount of the 13C from the leucine tracer was bioconverted into the lipid pool. The mean δ13C of the lipids in control populations (populations that were not exposed to any 13 C-tracers) of cockroaches and crickets (-22.4‰) was not statistically different from the mean δ13C of the lipids in cockroaches and crickets in the 13C-leucine treatment (-22.0‰; t-test, df = 14, p = 0.107). We did not raise parallel, control populations of the other species, but we assume the basic biochemistry of these insects is generally similar. The minimal ‘leakage’ (sensu [35]) of the 13C from the leucine tracer was similar to that reported for mice raised for seven weeks on 13C-leucine tracers. A small amount of the 13C from the palmitic acid tracer was recovered in the lean tissues of the insects. The mean δ13C of the lean tissue in control populations of cockroaches and crickets (-18.5‰) was statistically different from the mean δ13C of the lean tissue in cockroaches and crickets in the 13C-palmitic acid treatment (-12.9‰; t-test, df = 14, p < 0.001). This extent of 13 C leakage from the lipid pool into the lean pool was greater than previously reported in mice raised on 13C-palmitic acid [35], yet it remains unclear precisely how the 13C from the palmitic acid tracer was partitioned between the carbohydrate and protein components of the lean tissue fraction because we did not analyze these fractions separately. Compound specific stable isotope analyses would be useful to determine how the palmitic acid-derived 13C atoms become distributed among non-lipid components [61–63]. Nevertheless, we estimate that >95% of the 13 C atoms from the palmitic acid tracer remained within the lipid pool of the body, and conclude that the δ13C in the exhaled breath of the palmitic acid treatment groups was an effective proxy of endogenous lipid oxidation during starvation.

What strategies contribute to improved starvation tolerance? The LT50 ranged from 3 days in moth larvae to 52 days in adult cockroaches. Comparisons of starvation tolerance across studies are difficult given the dearth of values reported in literature for these species and life stages. American cockroaches apparently begin to succumb to starvation within two weeks [17,64], and all died by 42 days [65]. Many of the cockroaches in this study lived beyond 60 days. Studies of Gryllus crickets report that they are capable of surviving starvation for two days longer than LT50 of the Acheta species in the present study [15,26]. While we did observe a few crickets tolerating at least seven days of starvation we do not consider these to be representative of the general population. Some crickets and cockroaches are known to reduce their locomotor activity during starvation [26,65]. The crickets and the cockroaches in this study were maintained in groups, and not individually, which may have increased activity and affected their apparent starvation tolerance. We eventually improved our sampling protocols so that we could measure the breath on individuals of the other three focal species. The three-day LT50 for the penultimate instar moth larvae is not surprising as other work has shown that these moths enter their last larval instar with almost no fat reserves (Helm and Davidowitz, unpublished data). A superficial perspective reveals that starvation tolerance in this study was positively correlated with body mass, but we consider this to be a spurious correlation and an artifact of our

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selection of two large species and three species (or life stages) that were an order of magnitude smaller (see Methods). Positive correlations have been made between starvation tolerance and body mass in Drosophila [21], ant lion larvae [8], and backswimmers [14], but bumble bees show the opposite relationship [66], and we have no evidence that body size in insects is optimized to improve starvation tolerance as it may in mammals [67,68]. Measures of starvation tolerance among other insect species will be useful to confirm this. Researchers recently developed a dynamic energy budget model to describe different physiological responses to starvation in insects [14]. The model includes three strategies that insects might employ including 1) reducing somatic maintenance costs, 2) maximizing the mobilization of endogenous nutrients, and 3) regulating energy mobilization to only pay for maintenance costs. It was not an objective of this study to document the extent to which these insects engaged in starvation-induced hypometabolism as has been done for many vertebrate species (reviewed in [3,69]). One study on starving Gryllus crickets found that they did not reduce metabolic rates during prolonged starvation [15], but future studies designed to document changes in standard metabolic rates and activity levels will be useful to document energy saving strategies during starvation in other species. Nevertheless our results do provide insight into the latter two, mutually exclusive, starvation strategies. If the starving insects were maximizing the rates of nutrient oxidation, we would expect to see evidence of increased protein and increased lipid oxidation at the onset of starvation. While the larval beetles exhibited a response weakly resembling this strategy, all of the other species exhibited inverse changes in endogenous protein and lipid oxidation that are suggestive of physiological regulation and not a state where all possible fuels were maximally oxidized. The insects in this study exhibited varying strategies with regard to the regulation of fuel oxidation. Are these differences related to their ability to withstand starvation? We found several correlations between survival time (LT50) and particular performance metrics (Fig 3A). The strongest of these was a linear relationship between LT50 and proteinpeak. The relationship between LT50 and proteinpeak was isometric supporting the long-standing idea that starvation tolerance is generally limited by an unregulated increase in protein oxidation. But the strategies occurring during the earlier phases of starvation might play a role in delaying this reliance on protein. If we assume that the five species used in this study are representative of insects in general (an assumption that needs to be tested in future studies), then correlations between the starvation tolerance and duration of protein sparing and the timing of maximal lipid oxidation (lipidpeak) could offer insight into variation in starvation tolerance. In particular, all of the species besides the cockroaches exhibited roughly isometric relationships between sparingduration and lipidpeak versus LT50 (Fig 3B and 3C). Interestingly, the values for the cockroaches did not follow these linear relationships, suggesting possible mechanisms responsible for the comparatively high starvation tolerance in the cockroaches. While each of the aforementioned relationships are correlative, they provide a basis for formulating hypotheses and predictions about which particular physiological strategies are responsible for differences in the starvation tolerance among insects. Future comparisons among the starvation strategies of other insects that exhibit high and low tolerances to starvation could be useful to examine this possibility. It would also be informative to correlate the timing of these physiological events with variation in starvation tolerance within conspecifics at the same life stage that may differ in their adiposity (sensu [70,71]); unfortunately, this would involve destructive sampling that would not be compatible with breath testing. Starvation strategies of insects, like other life history traits, appear to be shaped in part by the life stage [60]. The adult cockroaches, grasshoppers, and crickets tended to exhibit inverse patterns of oxidation of their lipids and proteins. These species are income breeders and would normally allocate ingested food among the demands associated with maintenance, locomotion,

PLOS ONE | DOI:10.1371/journal.pone.0140053 October 14, 2015

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and reproductive activity. However, many other insect species are capital breeders and may normally fast (sensu [72]) during adulthood [73]. It would be useful to characterize how those species partition their lipids and proteins to meet energy demands during adulthood. Growth is an imperative component of the life history of larval insects and the two larval species examined in this study exhibited comparatively low reliance on protein oxidation during starvation, suggesting that larval insects maximize protein sparing to support larval growth. Future studies comparing the starvation strategies among the different life stages of both holometabolous and hemimetabolous species will be useful to characterize how starvation strategies may change ontogenetically.

Conclusion The findings of this study underscore the growing awareness among comparative physiologists that starving animals do not necessarily follow the classic paradigm that canalizes the physiological progression into three discrete phases [74,75]. In fact, only two of the five species exhibited any evidence of sharply increased rates of protein oxidation immediately preceding death as predicted by Lusk (1928) and since retained as part of the paradigm in nutritional physiology [39]. Although there is a need for additional comparative studies of starvation physiology among many key groups of vertebrates and insects [76,77], the diverse responses we describe here raise the possibility that insects employ a broader range of strategies for regulating lipid and protein use than expected. Furthermore, the ability to regulate critical transitions in lipid and protein mobilization may help explain the differences in starvation tolerance, especially the physiological responses that immediately precede death. In addition to characterizing starvation responses in other insect species it will be important to explore the evolutionary underpinnings of this remarkable physiological diversity in the context of phylogenetic relationships and ecological factors.

Acknowledgments We thank Joey Sandoval, Evelyn Oliva, and Crystal Lafleur for helping rear the insect populations and collect breath samples and Autumn Moore for the carbon isotope measures of the solid samples. We are grateful to John Hatle for providing us with grasshopper nymphs.